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research communications
Acta Cryst. (2017). F73, 657–663 https://doi.org/10.1107/S2053230X17015941 657
Received 31 August 2017
Accepted 1 November 2017
Edited by N. Strater, University of Leipzig,
Germany
Keywords: fluorescence; trace fluorescent
labeling; low-cost imaging; protein
crystallization.
A low-cost method for visible fluorescence imaging
Crissy L. Tarver and Marc Pusey*
Department of Biological Science, University of Alabama in Huntsville, Huntsville, AL 35899, USA. *Correspondence
e-mail: [email protected]
A wide variety of crystallization solutions are screened to establish conditions
that promote the growth of a diffraction-quality crystal. Screening these
conditions requires the assessment of many crystallization plates for the
presence of crystals. Automated systems for screening and imaging are very
expensive. A simple approach to imaging trace fluorescently labeled protein
crystals in crystallization plates has been devised, and can be implemented at a
cost as low as $50. The proteins �-lactoglobulin B, trypsin and purified
concanavalin A (ConA) were trace fluorescently labeled using three different
fluorescent probes: Cascade Yellow (CY), Carboxyrhodamine 6G (CR) and
Pacific Blue (PB). A crystallization screening plate was set up using
�-lactoglobulin B labeled with CR, trypsin labeled with CY, ConA labeled
with each probe, and a mixture consisting of 50% PB-labeled ConA and 50%
CR-labeled ConA. The wells of these plates were imaged using a commercially
available macro-imaging lens attachment for smart devices that have a camera.
Several types of macro lens attachments were tested with smartphones and
tablets. Images with the highest quality were obtained with an iPhone 6S and an
AUKEY Ora 10� macro lens. Depending upon the fluorescent probe employed
and its Stokes shift, a light-emitting diode or a laser diode was used for
excitation. An emission filter was used for the imaging of protein crystals labeled
with CR and crystals with two-color fluorescence. This approach can also be
used with microscopy systems commonly used to observe crystallization plates.
1. Introduction
The structure and function of many proteins are often deter-
mined by X-ray crystallography, which requires crystals with
high regularity. Crystallization conditions that facilitate the
growth of a single crystal that diffracts to atomic resolution
must be ascertained by screening an assortment of solutions.
Screening conditions involves setting up multiple plates of
trial conditions and then periodically reviewing these condi-
tions for the growth of crystals. The reviewing process may be
carried out manually using a microscope, or it may be
performed using an automated plate-imaging system. There
are two major difficulties in the plate-reviewing process:
distinguishing macromolecule crystals from salt crystals and
the actual detection of macromolecule crystals. Automated
imaging systems address these difficulties by focusing the
detection approach on characteristics that are likely to be
present in macromolecules but not small molecules, such as
the presence of tryptophan. Imaging approaches based on
recognizing crystals, typically an extensive process, have some
of the same difficulties as direct visual observation. Most
recently developed methods now use fluorescence or some
other optical manipulation to clearly reveal the presence of
macromolecule crystals.
ISSN 2053-230X
An early approach was to make use of the intrinsic fluor-
escence in macromolecules (Judge et al., 2005; Dierks et al.,
2010) arising primarily from the presence of the amino acid
tryptophan. The use of UV is not recommended for direct
microscopy visualization. Two-photon fluorescence has been
used with an excitation wavelength of 515 nm (Madden et al.,
2011). This method requires scanning a high-intensity light
source through a region of interest, using a high numerical
aperture lens to achieve a sufficiently high photon density that
fluorescing molecules can absorb two photons, at twice the
wavelength of the normal absorption, within 10�15–10�16 s of
each other (Xu & Webb, 1997). This requires a high-power
light source plus a means of scanning the light through the
sample and acquiring the emission signal from each scanned
point. Another approach is the use of second-order nonlinear
imaging of chiral crystals, also known as SONICC (Kissick et
al., 2010). A different fluorescence approach is based upon
visible-light excitation of native fluorescence (Lukk et al.,
2016). The fluorescence is apparently not chromophore-
dependent, but is believed to be based on conjugated double
bonds and electron delocalization from crystal packing. The
fluorescence can be obtained over a range of visible wave-
lengths, but was found to be strongest with excitation at
<405 nm, with a rather wide Stokes shift (excitation at
�405 nm, emission at �485 nm). The fluorescence dramati-
cally increased with decreasing temperature and varied from
protein to protein. Some proteins were found to not fluoresce.
A relatively low-cost approach (<1000 Euro) has been
described by Watts et al. (2010). This approach is based on the
increase in fluorescence when a soluble probe, in this case
1-anilinonaphthalene-8-sulfonic acid (1,8-ANS), binds to
hydrophobic regions, as described by Groves et al. (2007).
The trace fluorescent labeling (TFL) approach was, as with
the above methods, introduced to speed up and simplify the
process of finding macromolecule crystals in screening plates
and to differentiate macromolecule crystals from salt crystals
(Forsythe et al., 2006). Relatively simple instrumentation can
be used, and the technique is not dependent upon the
presence of fluorescing amino acids as the fluorescent probe is
covalently bound to the protein. The safety issues associated
with UV fluorescence are avoided, and one can choose from a
range of colors when using visible fluorescence. The labeling
method is simple and takes about 15 min to carry out, and the
target labeling level of 0.1–0.5% is achieved if it is performed
according to protocol (Pusey et al., 2015). Labeling at this level
has been shown to not affect the nucleation rate or the
diffraction quality of the crystals obtained (Forsythe et al.,
2006).
The primary barrier to the use of all fluorescence-based
methods is the cost of the required instrumentation. Relatively
low-cost fluorescence microscopy systems can be obtained;
however, they are more suited for looking at slide-mounted
specimens instead of crystals in thicker and larger crystal-
lization plates. While fluorescence may be the most unam-
biguous means of identifying macromolecule crystals and
crystallization conditions, it is not readily available to smaller
structural biology research groups or students. Here, we
present a simple and low-cost approach to visible fluorescence
imaging of TFL crystallization screening plates.
2. Materials and methods
2.1. Proteins
The proteins used throughout this work were trypsin
(Sigma, catalog No. T1426), �-lactoglobulin B (Sigma, catalog
No. L8006) and concanavalin A (ConA). ConA was purified
in-house from jack beans using the method of Agrawal &
Goldstein (1967). The purified ConA was stored in crystalline
form at 4�C. An aliquot of the precipitate was removed,
concentrated by centrifugation, dissolved in weak ammonium
hydroxide solution and underwent buffer exchange using a
centrifugal desalting column into the crystallization buffer
0.025 M Na HEPES, 0.025 M NaCl pH 7.5.
2.2. Crystallization
Each protein was trace fluorescently labeled (TFL) as
described previously (Pusey et al., 2015) using either Cascade
Yellow (CY; Invitrogen, catalog No. C-10164), Carboxy-
rhodamine 6G (CR; Invitrogen, catalog No. C-6157) or Pacific
Blue (PB; Invitrogen, catalog No. P-10163). Crystallization
plates were set up using (i) CY-labeled ConA, (ii) CR-labeled
ConA, (iii) PB-labeled ConA, (iv) a mixture containing 50%
research communications
658 Tarver & Pusey � A low-cost method for visible fluorescence imaging Acta Cryst. (2017). F73, 657–663
Figure 1Top: diagram of the cell-phone-based fluorescence imaging system. (a)Cell phone; (b) emission filter; (c) 10�macro lens with attached hood; (d)LED mounted in lens hood. Not shown are the aluminium tube used tohold and aim the LED, the LED power supply and the clip that holds theassembly to the cell phone. Bottom: image of the complete cell-phone-based system, showing the macro lens with black hood attached to aSamsung Galaxy cell phone. Also shown are the power supply and theconnections to the LED.
PB-labeled ConA and 50% CR-labeled ConA, (v) CR-labeled
�-lactoglobulin B and (vi) CY-labeled trypsin. The sitting-
drop vapor-diffusion method was used for all crystallizations.
ConA was crystallized using the JCSG-plus screen (Molecular
Dimensions, catalog No. MD1-37) in Corning CrystalEX
plates (Hampton Research, catalog No. HR8-140). Each of the
96 reservoirs was filled with 50 ml precipitant solution, and the
three wells were prepared at protein:precipitant ratios of 1:1,
2:1 and 1:2. All plates were stored at room temperature.
Trypsin was crystallized using the conditions given on the
Rigaku website (http://www.rigaku.com) and �-lactoglobulin
B was crystallized from 0.1 M sodium citrate, 3.0 M ammo-
nium sulfate pH 4.0.
2.3. Fluorescent imaging
The imaging lens used was an AUKEY Ora 10� macro lens
purchased from Amazon (Fig. 1). The lens clips onto the
camera of a smartphone or tablet, and it comes with a hood.
The hood was modified by epoxying a short piece of 5 mm
internal diameter aluminium tubing to a hole drilled in the top
of the hood, near to where it attaches to the lens assembly.
When applying the epoxy, the aluminium tubing was aimed to
the center of the hood by a second piece of aluminium tubing
with a 5 mm outer diameter to indicate the path of the exci-
tation beam. After the epoxy had set, the exterior of the hood
was covered with a coating of flat black paint. The excitation
source used to screen crystallization plates containing protein
labeled with Cascade Yellow or Pacific Blue was a 5 mm light-
emitting diode (LED; LED Supply, catalog No. L3-0-
U5TH15-1; Fig. 2). This LED has a peak wavelength of 400 nm
and an emission half-angle of �15�. Power to the LED was
supplied by a 5 V power supply through a DynaOhm DC
resistor module (LED Supply, catalog No. 04006–020) to
control the LED current to 20 mA. The LED plugs into a
connector and can be easily changed for one with a different
wavelength. Alternatively, a 532 nm diode laser was used for
excitation of protein crystals labeled with Carboxyrhodamine
6G. The monochromatic laser light was launched into a fiber
optic to bring it to the hood, where a cone of light was emitted
onto the imaging area. An emission filter suitable for the
fluorescent probe to be imaged was inserted between the
camera and the clip-on lens.
3. Results and discussion
3.1. Magnification lenses
Several commercially available clip-on macro lenses for
smart devices were obtained and evaluated for fluorescent
imaging applications. Images with the best overall quality for
the cost were obtained using an AUKEY Ora lens with an
iPhone 6S, and this lens provided a convenient means of
mounting an excitation light source. Modifications to accom-
modate an excitation source were simple to make. One source
of difficulty in using these clip-on lenses was stabilizing them
firmly over the center of the camera lens. The more expensive
Olloclip Macro Pro Lens for iPhones eliminated the stability
research communications
Acta Cryst. (2017). F73, 657–663 Tarver & Pusey � A low-cost method for visible fluorescence imaging 659
Figure 2Complete LED power supply and the components used in assembling this light source. The LED bulb, the wiring connector that the LED plugs into andthe LED current-limiting resistor are labelled A, B and C, respectively, and the individual components are shown in (a), (b) and (c).
difficulties, but introduced new difficulties with the placement
of an emission filter.
3.2. Fluorescent probes
This imaging approach was tested using several fluorescent
probes. Crystallization plates containing ConA labeled with
PB (excitation and emission at 404 and 455 nm, respectively)
were initially imaged through a bandpass filter (Edmund
Optics, catalog No. 65-626). Subsequent experiments indicated
that the filter was not necessary, resulting in this system having
the fewest components and the lowest cost. Protein crystals of
ConA TFL with PB were excited with a 400 nm blue LED and
imaged without the use of an emission filter (Fig. 3a). These
crystals failed to excite under the 532 nm green diode laser
(Fig. 3b).
The original implementation of this system used CR as the
fluorescent probe. The Stokes shift for CR is �28 nm (exci-
tation at �524 nm, emission at �552 nm), the LED peak
wavelength was �525 nm with a full-width at half-maximum
(FWHM) wavelength range of �30 nm, and the addition of a
550 nm high-pass emission filter (Edmund Optics, catalog No.
62-977) between the macro lens and the camera lens was
required. The wavelength spread of the LED resulted in a
significant amount of excitation light still passing through the
filter, which obscured the fluorescent signal. However, protein
crystals of CR-labeled ConA were detected and imaged using
a 550 nm high-pass emission filter and a 532 nm diode laser as
an excitation source (Fig. 3c). The monochromatic laser light
was launched into a fiber optic to bring it to the optical port,
where a cone of light was emitted onto the imaging area.
These crystals failed to fluoresce with the 400 nm blue LED
(Fig. 3d).
Use of this approach is not limited to the fluorescent probes
mentioned. LEDs are available with emission peaks suffi-
ciently close to those of most fluorescent probes. Fluorescence
visualization is simplified when using probes having a larger
Stokes shift, but with some forethought those having a rela-
tively narrow shift can be accommodated, as shown in this
work. One important consideration is that fluorescent probes
are often very sensitive to their local environment and may
undergo absorption and/or emission shifts as a result.
research communications
660 Tarver & Pusey � A low-cost method for visible fluorescence imaging Acta Cryst. (2017). F73, 657–663
Figure 3(a) Crystals of ConA labeled with the fluorescent probe PB and excited using a 400 nm blue LED without using an emission filter. (b) The well shown in(a) imaged using a 532 nm green laser diode and a 550 nm high-pass emission filter. (c) CR-labeled ConA crystals imaged using a 532 nm green laserdiode and a 550 nm high-pass emission filter. (d) The well shown in (c) imaged under the light from a 400 nm blue LED without an emission filter.
However, this may be mitigated by the fact that the probe will
be buried in the relatively protected environment of the
crystal, potentially precluding effects originating from the
bulk solution.
3.3. Emission filters
In the case where the Stokes shift of the fluorescent probe
was very narrow, emission filters were needed to prevent
reflected excitation light from overwhelming the fluorescent
signal. The filters needed to have a very sharp cutoff and a
very high blocking optical density at nontransmission wave-
lengths to minimize reflections obscuring the fluorescence
emission. However, the use of a filter more than quadrupled
the cost of the system. Two variations of a laser-excitation
approach were tried: manually directing a green laser pointer
through the translucent hood around the lens and directing
the beam into a fiber optic that was passed through a close-
fitting aluminium tube through the hood. In both cases the
550 nm high-pass filter was required to block excitation
reflections from the camera. While both approaches work, it
was felt that switching to a diode laser-excitation source
detracted from the goal of an inherently simple low-cost
imaging system. However, use of a laser-excitation source does
facilitate imaging fluorescence from probes having a very
small Stokes shift.
Although some excitation light enters the camera with the
filter-free approach used with PB, it is somewhat attenuated by
the glass optics of the macro lens and it is readily differ-
entiated from the emission signal. PB has a sufficiently wide
Stokes shift that an emission filter was not needed, although
one could be used to further enhance the fluorescence over
the background. The fluorescent probe CY (excitation at
�410 nm, emission at �560 nm) can also be excited using a
400 nm LED. Owing to the similarities between the CR and
CY emission peaks, the 550 nm high-pass filter used with CR
was tested with CY (results not shown). As with PB, the use of
an emission filter was not necessary for imaging protein
crystals labeled with CY. One negative aspect of the use of CY
was the fact it is no longer commercially available. The
fluorescent probe Pacific Orange (PO; Invitrogen, catalog No.
P-30253; excitation at �405 nm, emission at �551 nm) is
commercially available and could be used with the same
excitation LED.
3.4. Two-color fluorescence
The method can also be used for two-color fluorescence,
which is useful for the visualization and imaging of complexes.
This approach required the use of an emission filter. Crystal-
lization screening plates were set up using (i) ConA labeled
with PB, (ii) ConA labeled with CR and (iii) a mixture
containing 50% PB-labeled ConA and 50% CR-labeled
ConA. Screening plates containing CR-labeled ConA were
imaged using a 532 nm green diode laser through a fiber optic
as the excitation source and a 550 nm emission cutoff filter.
Crystallization plates containing PB-labeled ConA were
imaged using a 400 nm LED without an emission filter. The
screening plate created using a combination of two fluorescent
probes was imaged using both sets of optics. A single well
containing protein crystals was imaged under white light
(Fig. 4a), the CR optics (Fig. 4b) and the PB optics (Fig. 4c).
Other pairs of fluorescent probes may be employed for two-
color fluorescence. The ability to distinguish the fluorescence
of one probe in the presence of the other is essential. Costs
will be higher owing to the required emission filter(s). LEDs
typically have a full-width half-maximum wavelength spread
of��15�. There is still considerable excitation light relative to
the fluorescence signal at the �0.1–1% intensity level at the
peak fluorescence wavelength for probes with a short Stokes
shift. Use of probes with a longer Stokes shift, for example PB
and CY, can ameliorate this problem. The other approach, as
taken here, is to use a monochromatic light source. While this
adds to the complexity, diode lasers can be obtained online at
research communications
Acta Cryst. (2017). F73, 657–663 Tarver & Pusey � A low-cost method for visible fluorescence imaging 661
Figure 4Two-color fluorescence imaging. (a) Protein crystals of ConA labeled with the fluorescent probes CR and PB under white light. (b) Image of the wellshown in (a) under the light of a 532 nm green laser diode using a 550 nm high-pass emission filter. (c) Image of the well shown in (a) illuminated with a400 nm blue LED with no emission filter.
a lower cost than that of emission filters. However, emission
filters are still sometimes needed to keep reflected light out of
the image.
3.5. Proteins
In order to examine this imaging method with additional
proteins, crystals of �-lactoglobulin B and trypsin were
photographed. �-Lactoglobulin B and trypsin crystals were
imaged under white light (Figs. 5a and 5c). The same
�-lactoglobulin B well was photographed again using the same
532 nm green diode laser, fiber optic and 550 nm emission
cutoff filter as used to image CR-labeled ConA crystals
(Fig. 5b). CY-labeled trypsin crystals were imaged using a
400 nm blue LED for excitation without an emission filter
(Fig. 5d).
3.6. Imaging
All fluorescent images were acquired using an iPhone 6S.
However, the use of this method is not limited to cell phones.
The clip-on lens can be applied to most devices with a camera,
but the camera has to be capable of accommodating the macro
optics. If image capture is not desired and an emission filter is
not needed, then one can bypass the use of a camera. Fluor-
escing crystals can be observed by manually placing the hood
with a mounted LED over a plate of TFL crystals and viewing
them under a low-powered microscope (a microscope that is
normally used to manually review crystallization plates).
Fluorescence from crystals at least as small as 10 mm can be
visualized in a dark room and, depending upon the microscopy
system, one can zoom in for higher magnification imaging. The
room does not have to be totally dark, but it is necessary to
remove reflected light from overhead fluorescent lights. In
fact, it was discovered that one can directly see CY-labeled
crystals without the use of a microscope. However, this is not a
practical approach when using probes that require near-UV
wavelengths for excitation. If the microscope has a camera
port then it can also be used for image capture. Low-cost
means of attaching a cell phone to microscopy or other
imaging systems are also commercially available.
This method was tested using several imaging devices. The
iPhone 6S contained the most versatile imaging system with
internal filters, and it provided the best quality images. Several
different macro lenses were tested, and the AUKEY Ora lens
research communications
662 Tarver & Pusey � A low-cost method for visible fluorescence imaging Acta Cryst. (2017). F73, 657–663
Figure 5(a) Crystals of CR-labeled �-lactoglobulin B under white light. (b) The well shown in (a) imaged using a 532 nm green laser diode and a 550 nm high-passemission filter. (c) CY-labeled trypsin crystals under white light. (d) The well shown in (c) imaged under a 400 nm blue LED without an emission filter.
was found to perform the best at a low cost. The presence of
the hood served to reduce background illumination and it was
a convenient mounting point for the excitation light. Crystals
as small as 10 mm could be imaged, and possibly smaller with
the use of higher magnification optics. Other clip-on macro
lenses are commercially available and may be more suitable
for certain imaging devices.
While not tested, the method of Lukk et al. (2016) may be
accommodated by the approach described here. The apparent
Stokes shift for excitation at 405 nm is�80 nm. The excitation
source for their work was a 5 mW laser. If the added cost (and
complexity) is acceptable then the LED can be replaced by a
405 nm diode laser, bringing the light into the hood using a
fiber optic through the same aluminium tube as used for the
LED. However, not all proteins fluoresce. The advantage of
the TFL approach over other fluorescence methods is that the
fluorescence probe, and thus a signal, will be present. Previous
work has clearly shown that the presence of the probe at the
target labeling concentration range of 0.1–0.5% will not affect
the nucleation rates or quality of the diffraction data obtained
(Forsythe et al., 2006).
3.7. Costs
The cost of a simple system, composed of an imaging lens
and LED (Fig. 1) is less than $50. The cost can be less than $30
depending on the source of the LED, the power supply and
how the current-limiting resistor is implemented. The
approach taken can potentially be applied to UV fluorescence,
but at increased cost driven by the higher price of UV LEDs.
Other variations are possible, such as the use of low-cost diode
lasers for the excitation source, as demonstrated here for
imaging CR-labeled proteins. This approach involves a more
complex hardware setup as well as the higher cost of the laser
and fiber optic. An emission filter may be required to keep
reflected laser light noise out of the signal.
Most automated imaging systems are very expensive. The
method of Watts et al. (2010) is closest to our method in cost at
less than 1000 Euro. Their approach used the increase in the
fluorescence of the dye 1,8-ANS (excitation at �360 nm and
emission at �505 nm) upon diffusing into and binding to the
interior of a protein crystal (Groves et al., 2007). In their
implementation, the whole plate was imaged, with each well
being excited using a separate LED. The excitation source was
directed towards the imaging optics while utilizing both
excitation and emission filters. Their design also used
crystallization-plate-specific masks to limit the excitation light
to only the crystalline-drop positions. Software filtering was
used to reduce the background noise. As the method relies
upon free probe diffusing into the crystal, it cannot be used for
multiple colors. In comparison, the method presented here is a
low-cost approach for anyone owning a smart device with a
camera. It provides a way to rapidly screen plates containing a
wide variety of crystallization solutions and image protein
crystals. This approach can also be used for the imaging of
complexes, which can save beam time.
Several potential improvements immediately became
apparent using this method. When using an autofocusing
device, the camera must be securely fixed in position to more
easily obtain quality images. A Bluetooth shutter control and
tripod were later utilized to address this issue. While these
items did stabilize and improve the imaging system, they
increased the overall cost. Therefore, all images shown were
taken using a handheld iPhone 6S camera while resting the
lens hood on the crystallization plate. A second improvement
would be an application written for the smart device to adjust
the focal point and other exposure parameters, such as filters
that may be built into the camera.
Acknowledgements
The content is solely the responsibility of the authors and does
not necessarily represent the official views of the National
Institutes of Health.
Funding information
The research reported in this publication was supported by
National Institute of General Medical Sciences of the National
Institutes of Health under award No. R42GM116283.
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